Monoclonal antibodies with neutralizing activity against SARS-CoV-2 have demonstrated clinical benefits in cases of mild-to-moderate SARS-CoV-2 infection, substantially reducing the risk for hospitalization and severe disease1,2,3,4. Treatment generally requires the administration of high doses of these monoclonal antibodies and has limited efficacy in preventing disease complications or mortality among hospitalized patients with COVID-195. Here we report the development and evaluation of anti-SARS-CoV-2 monoclonal antibodies with optimized Fc domains that show superior potency for prevention or treatment of COVID-19. Using several animal disease models of COVID-196,7, we demonstrate that selective engagement of activating Fcγ receptors results in improved efficacy in both preventing and treating disease-induced weight loss and mortality, significantly reducing the dose required to confer full protection against SARS-CoV-2 challenge and for treatment of pre-infected animals. Our results highlight the importance of Fcγ receptor pathways in driving antibody-mediated antiviral immunity and exclude the possibility of pathogenic or disease-enhancing effects of Fcγ receptor engagement of anti-SARS-CoV-2 antibodies upon infection. These findings have important implications for the development of Fc-engineered monoclonal antibodies with optimal Fc-effector function and improved clinical efficacy against COVID-19 disease.
Several neutralizing monoclonal antibodies that target the SARS-CoV-2 spike protein have entered clinical testing over the past months, yielding US Food and Drug Administration approval of two monoclonal antibody cocktails—casirivimab and imdevimab, and bamlanivimab and etesevimab—for the treatment of patients with mild-to-moderate COVID-194. In phase II/III studies, these and other monoclonal antibodies that are currently awaiting regulatory approval have demonstrated clear therapeutic benefits in cases of mild-to-moderate COVID-19, reducing the risk for hospitalization1,2,3 by more than 80%. These results are in stark contrast to the findings from phase III trials (for example, ACTIV-3 and NCT04501978) that assessed the therapeutic activity of these monoclonal antibodies in hospitalized patients with COVID-19. In all cases, none of the tested monoclonal antibodies offered any therapeutic benefit, even when administered at exceedingly high doses or in combination with remdesivir5.
The antiviral activity of IgG antibodies is the outcome of Fab-mediated virus neutralization coupled with the capacity of the Fc domain to mediate effector functions through interactions with Fcγ receptors (FcγRs) expressed on effector leukocytes8. FcγR engagement mediates pleiotropic functions, including the clearance of viral particles9, cytotoxic elimination of virus-infected cells10 and induction of antiviral T-cell responses11. Several reports, using well-defined in vivo models of SARS-CoV-2 infection, have independently demonstrated that the antiviral activity of neutralizing anti-SARS-CoV-2 antibodies depends on Fc–FcγR interactions12,13,14,15. In addition, mechanistic studies have shown that these protective effects are mediated primarily by CCR2+ monocytes, as well as cytotoxic CD8+ T cells that infiltrate the lung and confer antiviral activities12. Despite these findings, no studies have tested whether optimization of neutralizing anti-SARS-CoV-2 monoclonal antibodies for enhanced FcγR binding could improve their therapeutic activity, especially in the setting of severe COVID-19. Maximizing the capacity of neutralizing anti-SARS-CoV-2 monoclonal antibodies to engage and activate the appropriate FcγR pathways is expected to lower the monoclonal antibody dose required for the treatment of mild-to-moderate COVID-19, as well as improve their activity in hospitalized patients.
Currently, most monoclonal antibodies in clinical use or development are expressed as human IgG1, which—despite its affinity for activating FcγRs—also exhibits binding to the inhibitory FcγRIIb, thereby limiting protective Fc-effector activities11. In addition, owing to presumptive safety concerns over the capacity of antibodies to exacerbate disease through antibody-dependent enhancement (ADE) mechanisms8, several clinical monoclonal antibodies (etesevimab, AZD8895 and AZD1061) have been engineered to lack FcγR-binding activity. However, despite numerous in vivo studies in animal models, there is no evidence for ADE12,13,14,15,16, and therapeutic administration of high doses of convalescent plasma or neutralizing anti-SARS-CoV-2 monoclonal antibodies in patients with COVID-19 has not been associated with worse disease outcomes1,2,3,5,17. Similarly, comparable safety profiles were evident in clinical trials of neutralizing monoclonal antibodies with intact or diminished Fc-effector function3,18,19.
Hamster FcγRs and IgG Fc-domain activity
To assess the role of FcγRs in the monoclonal antibody-mediated protection and develop monoclonal antibodies with superior therapeutic potency, we selected well-established small-animal models of SARS-CoV-2 infection that recapitulate the clinical features of human COVID-196,7,20. One of these models involves the use of Syrian hamsters (Mesocricetus auratus), a species that sustains productive SARS-CoV-2 replication and exhibits evidence of severe disease upon challenge6. However, a major obstacle in the study of human IgG Fc-effector activity is the substantial interspecies differences in the affinity of human IgG antibodies for FcγRs expressed by rodent species such as hamsters21. We therefore cloned the four classes of hamster FcγRs and characterized their affinities for human, hamster and mouse IgG subclasses and Fc variants (Fig. 1a, b, Extended Data Fig. 1). Comparative analysis of hamster FcγRs revealed substantial sequence homology to mouse FcγRs, with three hamster FcγRs (FcγRI, FcγRIII and FcγRIV) corresponding to activating FcγRs, whereas FcγRIIb represents the sole inhibitory FcγR.
To assess the contribution of Fc–FcγR interactions to monoclonal antibody-mediated protection, we selected neutralizing monoclonal antibodies that are in clinical use or development, including casirivimab and imdevimab (REGN cocktail22) and S309/VIR-783123 (Vir) and expressed them as human IgG1 or as Fc variants with defined affinity for hamster FcγRs. In agreement with recent reports12, we observed that when monoclonal antibodies are administered prophylactically, Fc-effector function shows minimal contribution to their antiviral activity (Fig. 1c). By contrast, in the therapeutic setting, wild-type, but not FcR-null (GRLR) variants, are able to suppress lung viremia and prevent weight loss (Fig. 1d). Because previous studies in mouse models of influenza and HIV-1 infection support a key role for FcγRIV in monoclonal antibody-mediated protection10,24, we compared the in vivo therapeutic activities of two Fc-domain variants—GAALIE and V11—that exhibit differential hamster FcγRIV-binding activity, but comparable affinity for the other hamster FcγRs (Fig. 1b). Whereas the FcγRIV-enhanced variant (GAALIE) demonstrates potent antiviral activity, no therapeutic activity is evident for V11, which exhibits minimal affinity for hamster FcγRIV (Fig. 1e–g).
SARS-CoV-2 in FcγR-humanized mice
Although these findings support the importance of Fc–FcγR interactions in monoclonal antibody-mediated protection against SARS-CoV-2 infection, their translational relevance is limited, given the structural complexity of the FcγR family and the divergence of these receptors between humans and other mammalian species21. To address this problem, we previously developed a mouse strain in which only human FcγRs are expressed in a pattern that recapitulates as faithfully as possible the expression pattern in human tissues25. Despite differences in the absolute FcγR expression levels between humans and FcγR-humanized mice (for example, the expression of FcγRI on neutrophils and FcγRIIb on monocytes), this strain represents a suitable platform for studies on human IgG antibody function with translational relevance to humans. Human FcγR expression among the various leukocyte populations is stable and does not differ between young and old mice (Extended Data Fig. 2). Infection of old (more than 15-week-old), but not young (7-week-old), FcγR-humanized mice with the mouse-adapted SARS-CoV-2 strain MA107 results in challenge-dose-dependent weight loss and mortality (Fig. 2a, b). Recent studies have determined that on day 2 after infection, MA10-infected mice exhibit peak lung viral titres, accompanied by severely compromised pulmonary function and extensive lung histopathologic damage7. Histological evaluation of lungs from MA10-infected FcγR-humanized mice (more than 15 weeks old) revealed multifocal areas of interstitial pneumonia, extensive inflammatory cell infiltration and occasional necrotic and proteinaceous material and hyalinized membranes within affected alveoli (Extended Data Fig. 3). Such histopathological findings are consistent with those observed in well-established animal models of SARS-CoV-2 infection used extensively in previous studies, and resemble the lung pathology of human COVID-197,12,13,14. Although it is not classified as a variant of concern, the MA10 strain contains several mutations near the epitopes targeted by monoclonal antibodies currently in clinical use or development. As a result, several of these monoclonal antibodies exhibit significantly reduced neutralizing activity against MA10, which is comparable to that observed for variants of concern such as B1.351 (Extended Data Fig. 4).
Fc-effector function in antibody therapy
In a model of monoclonal antibody-mediated therapy, we observed that the REGN monoclonal antibody cocktail (expressed as wild-type human IgG1) confers full protection of FcγR-humanized mice when administered at 5 mg kg−1 1 day after lethal challenge with MA10 (Fig. 2c–f). By contrast, no therapeutic activity is evident in mice lacking FcγRs (FcγR-null) or when monoclonal antibodies are expressed as variants (GRLR) with minimal affinity for human FcγRs, highlighting the importance of Fc-effector function in the therapeutic activity of neutralizing monoclonal antibodies (Fig. 2c–f). To determine the mechanisms by which human FcγRs contribute to the monoclonal antibody-mediated protection, REGN cocktail monoclonal antibodies were expressed as human IgG1 Fc variants11, and exhibit differential affinities for the various human FcγRs (Fig. 3a). As outlined in Fig. 3b, we assessed the therapeutic activity of Fc variants of the REGN monoclonal antibody cocktail at a dose (1 mg kg−1) at which wild-type human IgG1 confers minimal protection (Fig. 3c). Consistent with a protective role for activating FcγRs, Fc variants enhanced for either FcγRIIa (GA) or FcγRI and FcγRIII (ALIE) show a trend of improved therapeutic potency over wild-type IgG1, whereas maximal therapeutic activity was evident only for the GAALIE variant, which is enhanced for both FcγRIIa and FcγRIII and has reduced affinity for the inhibitory FcγRIIb (Fig. 3d, e). These findings suggest that synergy between the two activating FcγRs—FcγRIIa and FcγRIII—probably accounts for the therapeutic activity of the GAALIE variant, which achieves the same degree of protection as wild-type IgG1, but at a fivefold lower dose. Additionally, the observed differences in the in vivo therapeutic activity among Fc variants could not be attributed to differences in their in vitro neutralization activity, antigen binding specificity or in vivo half-life (Extended Data Figs. 5, 6).
Notably, treatment of MA10-infected mice 1 day after infection with the GAALIE variant was not associated with enhanced disease, when administered at a low dose (1 mg kg−1) or at a much higher dose (40 mg kg−1) (Extended Data Fig. 7a). At this higher dose, which is typically used in the clinical setting, FcR-null variants (GRLR) also exhibit full protective activity similar to the GAALIE variants, suggesting that Fc-independent protection could be achieved once neutralizing monoclonal antibodies are administered at sufficiently high doses, as has been documented previously for other viral pathogens24. Similarly, treatment of SARS-CoV-2-infected mice two days after infection, which coincides with the peak of lung viral replication7, has no disease-enhancing effects and neither GAALIE nor GRLR variants offer any therapeutic benefit, confirming recent reports showing that the therapeutic window for neutralizing monoclonal antibodies is limited to 24 h after infection26 (Extended Data Fig. 7b).
Similar results were obtained when we assessed the in vivo therapeutic activity of another neutralizing anti-SARS-CoV-2 monoclonal antibody cocktail27 (C135 + C144 (also known as BMS-RU)) currently in clinical development27. When BMS-RU is administered to FcγR-humanized mice at 1 mg kg−1, only GAALIE variants, but not wild-type human IgG1 confer protective activity and prevent disease-induced weight loss (Fig. 3f, g). In contrast to neutralizing anti-SARS-CoV-2 monoclonal antibodies, Fc-engineering of the non-neutralizing anti-receptor-binding domain (RBD) monoclonal antibody CR3022 does not result in improved therapeutic activity, as neither CR3022-GAALIE nor CR3022 protected mice from lethal SARS-CoV-2 challenge (Fig. 3h).
Fc-domain activity in antibody prophylaxis
Our findings in hamsters suggest that when neutralizing monoclonal antibodies are administered prophylactically, Fc–FcγR interactions are not critical for their antiviral activity (Fig. 1c). However, given the substantial interspecies differences in FcγR biology between hamsters and humans, we assessed the contribution of activating FcγR engagement to the monoclonal antibody-mediated prophylaxis of MA10-challenged FcγR-humanized mice (Fig. 4a). When administered at a dose at which wild-type human IgG1 exhibits no protective activity (0.5 mg kg−1) (Fig. 4b), GAALIE variants of the REGN monoclonal antibody confer full protection against lethal SARS-CoV-2 challenge, suggesting that selective activating FcγR engagement could improve the efficacy of neutralizing monoclonal antibodies in both the therapeutic as well as in the prophylactic setting (Fig. 4c).
To maximize the translational relevance of our findings, this study focused on neutralizing anti-SARS-CoV-2 monoclonal antibodies that are currently in clinical use or development and assessed their in vivo protective activity in mouse strains that recapitulate the unique complexity of human FcγRs25. Challenge of FcγR-humanized mice with MA10 results in accelerated weight loss and significant mortality, resembling the clinical manifestations of severe COVID-19. However, such rapid symptomatic disease development limits the therapeutic window for monoclonal antibody treatment and does not allow full unravelling of the mechanisms of COVID-19 disease pathogenesis and the potential immunopathologies due to host immune-related responses. Despite this limitation, we observed that in models of monoclonal antibody-mediated prophylaxis or early treatment, Fc engineering for selective binding to activating FcγRs resulted in an approximately fivefold reduction in the monoclonal antibody dose required to achieve full therapeutic benefit; a finding consistent with our recent in vivo evaluation studies on Fc-optimized anti-influenza virus monoclonal antibodies11. Consistent with previous studies on other viral pathogens, including HIV-128, influenza24 and Ebola29, our findings suggest that FcγR—but not complement pathways—confer monoclonal antibody-mediated protection, as monoclonal antibodies lack protective activity in mice deficient for all classes of FcγRs (Fig. 2c, d). Moreover, Fc variants such as GAALIE, which exhibit diminished C1q-binding activity (Extended Data Fig. 8), demonstrate improved therapeutic efficacy compared with wild-type IgG1.
Analysis of IgG Fc glycan characteristics in hospitalized patients with COVID-19 has previously revealed an association of disease severity with increased levels of afucosylated glycoforms30,31, which exhibit increased affinity for the activating FcγRIII11. Although these results suggest a potential pathogenic effect for FcγRIII pathways, patients with severe COVID-19 are also characterized by delayed induction of neutralizing antibody responses accompanied by elevated antibody levels32, suggesting that any disease-enhancing effects of afucosylated antibodies might also be related to their poor neutralizing activity33. However, in our study, we did not observe any pathogenic or disease-enhancing effects of anti-SARS-CoV-2 monoclonal antibodies engineered for enhanced binding to activating FcγRs, irrespective of their neutralizing potency (Fig. 3). It is therefore probable that susceptibility to severe disease is not entirely driven by the FcγRIII-binding activity of anti-SARS-CoV-2 IgGs, but rather by multiple, complex immunological determinants.
Despite the successful deployment of highly effective vaccines, neutralizing anti-SARS-CoV-2 monoclonal antibodies are expected to continue to have an important role in virus-containment efforts and the clinical management of COVID-19, especially in high-risk populations and immunocompromised individuals. Although regulatory approval of anti-SARS-CoV-2 monoclonal antibody cocktails has been based on their remarkable clinical efficacy in patients with mild-to-moderate COVID-191,2,3, none of the currently approved monoclonal antibodies take full advantage of the potential of IgG molecules to mediate protective antiviral Fc-effector functions. Our findings provide a paradigm for the development of monoclonal antibody-based therapeutics with improved potency and superior therapeutic efficacy against COVID-19 through selective engagement of specific FcγR pathways.
Viruses, cell lines and animals
A P1 stock of the SARS-CoV-2 MA10 strain7 was amplified in VeroE6 cells obtained from the ATCC that were engineered to stably express TMPRSS2 (VeroE6-TMPRSS2). To generate a P2 working stock, VeroE6-TMPRSS2 cells were infected at a multiplicity of infection (MOI) of 0.1 pfu per cell and incubated at 37 °C for 4 days. The virus-containing supernatant was subsequently harvested, clarified by centrifugation (3,000g; 10 min), and filtered using a disposable vacuum filter system with a 0.22-μm membrane. Virus stock titres were measured by standard plaque assay on Huh-7.5 cells that stably express ACE2 and TMPRSS2 (Huh-7.5-ACE2/TMPRSS2). In brief, 500 μl of serial tenfold virus dilutions in Opti-MEM were used to infect 4 × 105 cells seeded the previous day into wells of a 6-well plate. After 90 min adsorption, the virus inoculum was removed, and cells were overlaid with DMEM containing 10% FBS with 1.2% microcrystalline cellulose (Avicel). Cells were incubated for 4 days at 33 °C, followed by fixation with 7% formaldehyde and crystal violet staining for plaque counting. To confirm virus identity and evaluate for unwanted mutations that were acquired during the amplification process, RNA from virus stocks was purified using TRIzol reagent (ThermoFisher). In brief, 200 μl of each virus stock was added to 800 μl TRIzol reagent, followed by 200 μl chloroform, which was then centrifuged at 12,000g for 5 min. The upper aqueous phase was moved to a new tube, mixed with an equal volume of isopropanol, and then added to an RNeasy Mini Kit column (Qiagen) to be further purified following the manufacturer’s instructions. Viral stocks were subsequently confirmed by Next Generation Sequencing using libraries for Illumina MiSeq.
The SARS-CoV-2 NYC isolate was obtained from a patient’s saliva generously provided by A. Viale (Memorial Sloan Kettering Cancer Center) and amplified in Caco-2 cells. This P1 virus was used to generate a P2 working stock by infecting Caco-2 cells at an MOI of 0.05 pfu per cell. Cells were incubated at 37 °C for 6 days before collecting virus-containing supernatant as described above. Similarly, virus stock titres were determined by plaque assay performed on Huh-7.5-ACE2/TMPRSS2 cells. All SARS-CoV-2 experiments were carried out in biosafety level 3 (BSL-3) containment in compliance with institutional and federal guidelines.
VeroE6 cells (ATCC, CRL-1586), Caco-2 cells (ATCC, HTB-37) and Huh-7.5 hepatoma cells34 were cultured in Dulbecco’s Modified Eagle Medium (DMEM) supplemented with 1% nonessential amino acids and 10% fetal bovine serum (FBS). The 293T cells (ATCC, CRL-3216) and HT1080-ACE2 (provided by P. Bieniasz (Rockefeller University)) were maintained in DMEM supplemented with 10% FBS, 50 U ml−1 penicillin and 50 μg ml−1 streptomycin (ThermoFisher). All cell lines were maintained at 37 °C at 5% CO2. Expi293F cells (ThermoFisher) were maintained at 37 °C, 8% CO2 in Expi293 expression medium (ThermoFisher) supplemented with 10 U ml−1 penicillin and 10 μg ml−1 streptomycin. Cell lines were not authenticated after purchase. All cell lines tested negative for mycoplasma contamination.
In vivo experiments were approved by the Rockefeller University Institutional Animal Care and Use Committee in compliance with federal laws and institutional guidelines. Hamsters and mice were maintained at the Comparative Bioscience Center at the Rockefeller University at a controlled ambient temperature (20–25 °C) and humidity (30–70%) environment with 12-h dark:light cycle. Golden Syrian hamsters were purchased from Charles River laboratories (strain code 049) and maintained in compliance with USDA regulations. FcγR knockout (mFcγRα−/−; Fcgr1−/−) and FcγR-humanized mice (mFcγRα−/−, Fcgr1−/−, hFcγRI+, hFcγRIIaR131+, hFcγRIIb+, hFcγRIIIaF158+ and hFcγRIIIb+) were generated in the C57BL/6 background and characterized in previous studies11,25.
Cloning, expression and purification of recombinant proteins
Human IgG1 Fc-domain variants were generated by site-directed mutagenesis using specific primers as previously described9, and recombinant IgG antibodies were expressed and purified using previously described protocols11. Purity was assessed by SDS–PAGE followed by SafeStain blue staining (ThermoFisher), as well as by size exclusion chromatography (SEC) using a Superdex 200 Increase 10/300GL column (GE Healthcare) on an Äkta Pure 25 HPLC system (data analysed using Unicorn v.6.3 software). All antibody preparations were more than 94% pure and endotoxin levels were less than 0.05 EU mg−1, as measured by the limulus amebocyte lysate assay.
The two plasmid-based HIV-NanoLuc-SARS-CoV-2 pseudovirus system35 was provided by P. Bieniasz (Rockefeller University). The S gene was modified by site-directed mutagenesis to introduce the amino acid changes present in the MA10 or the B.1.351 strains7. SARS-CoV-2 wild-type, MA10 and B.1.351 pseudovirus particles were generated by transfection of the two-plasmid-based system to 293T cells using X-tremeGENE HP DNA transfection reagent (Sigma).
Golden Syrian hamster FcγR cDNA sequences were identified based on the current M. auratus genome assembly (MesAur1.0) and recent transcriptomic data36. To validate sequences, hamster FcγR sequences were amplified and sequenced (Genewiz) from Syrian hamster spleen cDNA (Zyagen) using the following primers: hamster FcγRI (5′-GGCGGACAAGTGGTAAATGTCAC-3′, 5′-CGGACACATCATTGCTTCAGACTTACTAAG-3′), hamster FcγRII (5′-CTGCTGGGACACATGATCTCC-3′, 5′-TTAAATGTGGTTCTGGTAATCATGCTCTG-3′), hamster FcγRIII (5′-GAGTCTGGAGACACAGATGTTTCAG-3′, 5′-CGACGTCATTTGTCCCGAGG-3′), hamster FcγRIV (5′-AATGGGTGAGGGTGCTTGAG-3′, 5′-GAGGGAATGTTGGGGACAGG-3′). To identify the ectodomain, transmembrane and cytoplasmic domains, Syrian hamster FcγR protein sequences were then aligned against annotated mouse FcγR protein sequences (Uniprot). Soluble Syrian hamster FcγR ectodomains were generated by transient transfection as described above for monoclonal antibodies. Syrian hamster FcγR expression plasmids were generated encoding a secretion signal peptide, the predicted Syrian hamster FcγR ectodomain, and a C-terminal Strep or His tag. Following transfection of Expi293 cells, recombinant FcγRs were purified from cell-free supernatants by affinity purification using Strep-Tactin Superflow Plus resin (Qiagen) or Ni-NTA Agarose (Qiagen), per manufacturer’s instructions. Purified proteins were dialysed into PBS and assessed for purity by SDS–PAGE followed by SafeStain blue staining. Monomeric FcγR ectodomains were fractionated from aggregates by SEC on an Äkta Pure system using a Superdex 200 Increase 10/300 GL column (GE Healthcare).
Surface plasmon resonance
All experiments were performed with a Biacore T200 SPR system (GE Healthcare) at 25 °C in HBS-EP+ buffer (10 mM HEPES, pH 7.4, 150 mM NaCl, 3.4 mM EDTA, 0.005% (v/v) surfactant P20). IgG antibodies were immobilized on Series S Protein G sensor chip (GE Healthcare) at a density of 2,000 response units (RU). Serial dilutions of recombinant soluble hamster FcγR ectodomains were injected to the flow cells at 20 μl min−1, with the concentration ranging from 1,000 to 15.625 nM (successive 1:2 dilutions). Association time was 60 s followed by a 900-s dissociation step. At the end of each cycle, sensor surface was regenerated with a glycine HCl buffer (10 mM, pH 2.0; 50 μl min−1, 30 s). Background binding to blank immobilized flow cells was subtracted, and affinity constants were calculated using BIAcore T200 evaluation software v.2.0 (GE Healthcare) using the 1:1 Langmuir binding model.
Neutralization activity of IgG1 Fc-domain variants was measured as previously described35. In brief, HT1080-ACE2 cells were seeded in 96 U-well black plates 24 h prior to infection with SARS-CoV-2 wild-type, MA10 or B.1.351 pseudoviruses. Pseudovirus particles were pre-incubated with monoclonal antibodies (fourfold serially diluted starting at 10 μg ml−1) for 1 h at 37 °C and then added to a monolayer of HT1080ACE2 cells. Following a 48-h incubation at 37 °C, cells were carefully washed with PBS and lysed with Luciferase Cell Culture Lysis reagent (Promega) for 15 min. Nano luciferase activity was detected by adding Nano-Glo Luciferase Assay System (Promega) and measured by SpectraMax Plus spectrophotometer (Molecular Devices), using 0.5 s integration time. Data were collected and analysed using SoftMax Pro v.7.0.2 software (Molecular Devices). Relative luciferase units were normalized to those derived from cells infected with the relevant SARS-CoV-2 pseudoviruses in the absence of monoclonal antibodies.
Anti-SARS-CoV-2 RBD ELISA
Recombinant SARS-CoV-2 RBD was immobilized (1 μg ml−1) into high-binding 96-well microtitre plates (Nunc) and after overnight incubation at 4 °C, plates were blocked with PBS plus 2% (w/v) BSA for 2 h. After blocking, plates were incubated for 1 h with serially diluted IgG antibodies or serum samples (1:3 consecutive dilutions in PBS starting at 100 ng ml−1), followed by horseradish peroxidase-conjugated goat anti-human IgG (1 h; 1:5,000; Jackson Immunoresearch). Plates were developed using the TMB two-component peroxidase substrate kit (KPL) and reactions were stopped with the addition of 1 M phosphoric acid. Absorbance at 450 nm was immediately recorded using a SpectraMax Plus spectrophotometer (Molecular Devices) and background absorbance from negative control samples was subtracted. Data were collected and analysed using SoftMax Pro v.7.0.2 software (Molecular Devices).
Human and mouse C1q binding to IgG1 Fc variants was assessed following previously described protocols37. In brief, antibodies were serially diluted (100–0.046 μg ml−1) in PBS and coated overnight (4 °C) onto high-binding 96-well microtiter plates. After washing with PBS + 0.05% Tween-20, plates were blocked with 2% BSA. Normal mouse or human serum (3%) was added and incubated for 60 min with gentle shaking. For the detection of C1q binding, monoclonal mouse anti-C1q antibody (JL-1, Abcam) was added at 0.5 μg ml−1, horseradish peroxidase-conjugated goat anti-mouse IgG was used at a dilution of 1:5,000, and plates were developed and analysed as described above.
Quantification of serum IgG levels
Blood was collected into microvette serum gel tubes (Sarstedt) and serum was fractionated by centrifugation (10,000g, 5 min). IgG levels were determined by enzyme-linked immunosorbency assay (ELISA) following previously described protocols11.
In vivo SARS-CoV-2 infection models
All animal infection experiments were performed at the Comparative Bioscience Center of the Rockefeller University in animal biosafety level 3 (ABSL-3) containment in compliance with institutional and federal guidelines. Hamsters (6- to 8-week-old males) were anaesthetized with isoflurane (3%) in a VetFlo high-flow vaporizer followed by an intraperitoneal injection of a ketamine (150 mg kg−1) and xylazine (10 mg kg−1) mixture. Hamsters were challenged intranasally with 105 pfu SARS-CoV-2 (NYC isolate, 100 μl viral inoculum). Mice (males or females; 6–7 or 16–22 weeks old) were anaesthetized with a ketamine (75 mg kg−1) and xylazine (15 mg kg−1) mixture (administered intraperitoneally) before challenge with SARS-CoV-2 (MA10 strain, 104 pfu in 30 μl, intranasally).
No statistical method was used to predetermine sample size. On the basis of preliminary studies that determined experimental variation in survival following infection and monoclonal antibody treatment, we performed power calculations and determined that at least n = 6 animals per group is sufficient to detect differences among experimental groups (powered at 80% for 5% significance level; survival assessed by log-rank (Mantel–Cox) test).
After infection, animals were monitored daily and humanely euthanized by CO2 asphyxiation at endpoints authorized by the Rockefeller University Institutional Animal Care and Use Committee, including any of the following: marked lethargy or inactivity, severe respiratory distress or laboured breathing, inability to ambulate or weight loss of greater than 20% of baseline. Animals were randomized on the basis of age, sex and weight. Before treatment, we ensured that the mean weight, sex and age were comparable among the various treatment groups. The treatment groups were not blinded to the personnel involved in monitoring animal survival and weight upon challenge. For antibody-mediated prophylaxis, antibodies were administered intravenously one day before virus challenge, whereas for antibody-mediated therapy, antibodies were administered one day after infection. Antibody dose was calculated in mg kg−1 body weight.
Lungs from euthanized mice were instilled with 10% neutral buffered formalin and fixed overnight by submersion in 10% formalin. Fixed tissues were embedded in paraffin, sectioned at 4-μm thickness, and stained with haematoxylin and eosin. Sections of lung were microscopically evaluated by a board-certified veterinary anatomic pathologist and representative images were captured with an Olympus BX45 light microscope using an SC30 camera with the cellSens Dimension software.
Determination of lung viral titres
Hamsters were euthanized at the indicated timepoints following infection and lung weights were recorded. Lungs were lysed in Trizol (ThermoFisher) and dissociated in gentle MACS M tubes using the gentleMACS Octo Dissociator (Miltenyi Biotec). Samples were transferred into Phasemaker tubes (ThermoFisher) and chloroform was added (200 μl chloroform per ml TRIzol). After vigorous shaking, tubes were rested for 5 min and then centrifuged for 15 min at 12,000g at 4 °C. The aqueous phase containing the RNA was transferred into a new tube and RNA extraction was performed by using RNeasy mini kit (Qiagen). SARS-CoV-2 lung titres were determined by quantitative PCR with reverse transcription assay using TaqMan Fast Virus 1-Step Master Mix, specifically designed primers and a TaqMan probe that bind a conserved region in the nucleocapsid gene of SARS-CoV-2 (2019-nCoV_N1-F :5′-GACCCCAAAATCAGCGAAAT-3′; 2019-nCoV_N1-R: 5-TCTGGTTACTGCCAGTTGAATCTG-3′; 2019-nCoV_N1-P: 5′-FAM-ACCCCGCATTACGTTTGGTGGACC-BHQ1-BHQ1-3′). Quantitative PCR was performed using an Applied Biosystems QuantStudio 6 Flex cycler using the following parameters: 50 °C for 5 min, 95 °C for 20 s followed by 40 cycles of 95 °C for 3 s, and 30 s at 60 °C. Signal from unknown samples was compared to a known standard curve (obtained through BEI Resources, NIAID, NR-52358) and viral titres were expressed as RNA copies per mg tissue.
After lysis of red blood cells (RBC lysis buffer; Biolegend), cells were resuspended in PBS containing 0.5% (w/v) BSA and 5 mM EDTA and labelled with the following fluorescently labelled antibodies (all used at 1:200 dilution unless otherwise stated): anti-human FcγRIIa (clone IV.3)-FITC, anti-human FcγRIIb (clone 2B6)-Dylight650 (used at 5 μg ml−1), anti-B220-AlexaFluor700, anti-Gr1-BrilliantViolet421, anti-CD8β-BrilliantViolet510, anti-human FcγRI (clone 10.1)-BrilliantViolet605, anti-CD3-BrilliantViolet650 (used at 1:100 dilution), anti-CD11b-BrilliantViolet711, anti-CD4-BrilliantViolet785, anti-human FcγRIIIa/b (clone 3G8)-PE, and anti-NK1.1–PE–Cy7. Relevant isotype control antibodies were used and included: mouse IgG1 isotype control-Dylight650 (used at 5 μg ml−1), mouse IgG2b kappa isotype control–FITC, mouse IgG1 kappa isotype control–PE, mouse IgG1 kappa isotype control–BrilliantViolet605. Samples that were stained with isotype control antibodies were also blocked with unlabeled anti-FcγR antibodies as follow: anti-human FcγRI (clone 10.1), anti-human FcγRIIa (clone IV.3), anti-human FcγRIIb (clone 2B6), and anti-human FcγRIIIa/b (clone 3G8) (used at 10 μg ml−1 and incubated for 5 min before staining with fluorescently labelled antibodies). Samples were analysed on an Attune NxT flow cytometer (ThermoFisher) using Attune NxT software v3.1.2 and data were analysed using FlowJo (v10.7) software.
Raw data for all main and extended data figures are included in the manuscript as source files. Results from multiple experiments are presented as mean ± s.e.m. One- or two-way ANOVA was used to test for differences in the mean values of quantitative variables, and where statistically significant effects were found, post hoc analysis using Bonferroni (adjusted for multiple comparisons) test was performed. Statistical differences between survival rates were analysed by comparing Kaplan–Meier curves using the log-rank (Mantel–Cox) test. Data were collected and analysed with Microsoft Excel and GraphPad Prism v.9.1 software (GraphPad) and P < 0.05 was considered to be statistically significant.
Further information on research design is available in the Nature Research Reporting Summary linked to this paper.
Raw data for all main and extended data figures are included in the manuscript as source files. Source data are provided with this paper.
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We thank P. Smith, E. Lam, R. Peraza, L. Smith, A. M. Mozqueda and T. Martinez for technical assistance and for maintaining and genotyping the mouse colonies used in this study; all the members of the Laboratory of the Molecular Genetics and Immunology (Rockefeller University) for discussions; S. Borghi for providing the recombinant SARS-CoV-2 RBD; P. Bieniasz for providing the HT1080-ACE2 cell line and plasmids for generating pseudoviruses; A. Viale for providing the SARS-CoV-2 NYC clinical isolate; A. Ashbrook and G. McNab for advice on handling BSL-3 agents and processing of tissues from infected animals; D. Martinez for technical assistance; S. Carrasco; staff from the Laboratory Comparative Pathology for histopathology support (with funding from NIH Core Grant P30CA008748). Research reported in this publication was supported by the National Institute of Allergy and Infectious Diseases (R01AI137276, R01AI157155, U19AI111825, and R01AI145870) and the Bill and Melinda Gates Foundation (INV-023152). This work was in part made possible with funding from the G. Harold and Leila Y. Mathers Charitable Foundation, the Bawd Foundation and Fast Grants (www.fastgrants.org), a part of Emergent Ventures at the Mercatus Center, George Mason University. We acknowledge support from the Rockefeller University and Vir Biotechnology. The content is solely the responsibility of the authors and does not necessarily represent the official views of the NIH.
S.B. and J.V.R. are inventors on a patent (WO2019125846A1) describing the GAALIE variant and its use in therapeutic monoclonal antibodies. C.M.R. and J.V.R. are members of the scientific advisory board of Vir Biotechnology with equity interests.
Peer review information Nature thanks Patrick Wilson and the other, anonymous, reviewers for their contribution to the peer review of this work. Peer reviewer reports are available.
Publisher’s note Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
Extended data figures and tables
a, Syrian hamster FcγRs were cloned, and their sequences were determined. The FcγR ectodomains are underlined. b-e, The affinity of human IgG1 and Fc variants (b, e, SPR sensorgrams), as well as of mouse (c) and hamster (d) IgG subclass variants for the various classes of hamster FcγRs was determined by surface plasmon resonance (SPR), using soluble hamster FcγR ectodomains. n.d.b., no detectable binding.
Extended Data Fig. 2 Comparison of the FcγR expression levels in the various effector leukocyte populations between young and older FcγR humanized mice.
FcγR expression was assessed by flow cytometry in peripheral blood leukocyte populations from young (6-7 weeks old; orange) and older (17 weeks old; blue) FcγR humanized mice. a, Gating strategy to identify the various leukocyte populations, b, Representative histogram overlay plots of FcγR expression in young and older FcγR humanized mice. Corresponding isotype controls are indicated in lighter shade. c, Quantitation of FcγR expression (MFI, median fluorescence intensity subtracted from the respective isotype control) in various leukocyte populations. Results are from 4 or 5 mice per group for young and older mice, respectively.
Extended Data Fig. 3 Histopathological analysis of lung tissue from SARS-CoV-2-infected FcγR humanized mice.
Lungs from SARS-CoV-2-infected (MA10 strain, 104 pfu, i.n.) FcγR humanized mice (16-22 weeks old) were collected on day 4 post-infection and evaluated histologically to assess the pathological changes associated with SARS-CoV-2 infection. a, Uninfected mice were characterized by clear alveolar spaces and absence of inflammatory cell infiltrates (low magnification (left panel, 200x); high magnification (center and right panels, 400x). b, In contrast, SARS-CoV-2 infection was associated with perivascular and peribronchial mononuclear leukocyte infiltration (200x left; 400x center panel), as well as the presence of macrophages and neutrophils in alveoli and necrotic cellular debris in alveolar spaces (600x, right panel). c, In addition, SARS-CoV-2-infected mice exhibited perivenular mixed neutrophilic, histiocytic, and lymphocytic inflammation, reactive endothelium and extravasation of leukocytes (left panel, 400x), as well as foci of interstitial neutrophilic and macrophage inflammation with hemorrhage and single cell necrosis (center and right panels, 400x). Images are representative of one uninfected and six infected mice.
Extended Data Fig. 4 In vitro neutralization activity of anti-SARS-CoV-2 mAbs against SARS-CoV-2 strains.
Neutralization activity of REGN and BMS/RU mAbs (individual mAbs or as a cocktail) against SARS-CoV-2 pseudotyped reporter viruses was measured by in vitro neutralization assay. (a) In vitro neutralization curves and (b) IC50 values of REGN (upper panel) and BMS/RU (lower panel) against SARS-CoV-2 WT, MA10, or B.1.351. (c) Fold change of SARS-CoV-2MA10 and SARS-CoV-2B.1.351 IC50 was calculated over WT. n = 1 experiment performed in duplicates. (d) Cryo-EM structures of REGN10933 and REGN10987 complexed with SARS-CoV-2 (PDB: 6XDG) or C135 (PDB: 7K8Z) and C144 (PDB: 7K90) complexed with the SARS-CoV-2 spike trimer. Residues within the SARS-CoV-2WT RBD that are mutated in the SARS-CoV-2MA10 strain (Q493K, Q498Y, P499T) are indicated in magenta.
Extended Data Fig. 5 In vitro neutralization activity and antigenic specificity of Fc variants of anti-SARS-CoV-2 mAbs.
To confirm that changes in the Fc domain have no effect on the neutralization activity and Fab-mediated functions of anti-SARS-CoV-2 mAb, Fc domain variants were characterized in (a-c) in vitro neutralization assays using SARS-CoV-2MA10 pseudotyped reporter viruses and (d, e) in ELISA assays using SARS-CoV-2 RBD. n = 1 experiment performed in duplicates. (a, d) REGN and (b, e) BMS/RU mAb cocktails were expressed as Fc variants and their in vitro neutralization activity (a, b, c, IC50 values) and (d, e) antigenic specificity was compared among Fc variants.
(a) Size-exclusion chromatography (SEC) analysis of Fc variants to determine aggregate formation among Fc domain variants. The SEC elution profiles and abundance (percentage) of monomeric IgG is indicated for the different Fc variants. (b) Fc variants of the REGN mAb cocktail were administered (i.v.; 50 μg) to FcγR humanized mice and antibody serum levels were determined by ELISA at various time points after antibody administration. n= total of 3 mice per group from two independent experiments. Data are mean ± s.e.m.
Extended Data Fig. 7 High-dose treatment of SARS-CoV-2-infected FcγR humanized mice with anti-SARS-CoV-2 mAbs Fc variants enhanced for activating FcγR binding is not associated with enhanced disease.
(a) Following the experimental strategy in Fig. 3b, SARS-CoV-2-infected (MA10, 104 pfu, i.n.) FcγR humanized mice (n = 3 for PBS and n = 5 for mAb-treated groups) were treated (i.v.) with 40 mg/kg REGN mAb cocktail expressed as Fc variants with diminished (GRLR) or enhanced activating FcγR binding (GAALIE). (b) SARS-CoV-2-infected mice were treated with 10 mg/kg BMS/RU mAb cocktail expressed as Fc variants GRLR or GAALIE on day 2 post infection. n= total of 10 mice per group for PBS, n = 9 for GAALIE, and n = 6 for GRLR from two independent experiments Weight loss (mean ± s.e.m.) was compared between GRLR and GAALIE-treated groups by two-way ANOVA (Bonferroni post hoc analysis adjusted for multiple comparisons). NS, not significant. Red arrow indicates time point of mAb treatment post-infection.
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Yamin, R., Jones, A.T., Hoffmann, HH. et al. Fc-engineered antibody therapeutics with improved anti-SARS-CoV-2 efficacy. Nature 599, 465–470 (2021). https://doi.org/10.1038/s41586-021-04017-w
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